Skip to main content
Download PDF

Seroprevalence and risk factors for lumpy skin disease virus seropositivity in cattle in Uganda

BMC Veterinary Research volume 15, Article number: 236 (2019) Cite this article

Abstract

Background

Lumpy skin disease (LSD) is a transboundary cattle disease caused by a Capripoxvirus of the family Poxviridae. In Uganda, documented information on the epidemiology of the disease is rare and there is no nationwide control plan, yet LSD is endemic. This study set out to investigate the seroprevalence of lumpy skin disease and determine the risk factors for LSD seropositivity, by carrying out a cross-sectional study in 21 districts of Uganda.

Results

A total of 2,263 sera samples were collected from 65 cattle herds and an indirect ELISA was used to screen for lumpy skin disease virus (LSDV) antibodies. We used univariable and multivariable mixed effect logistic regression models to identify risk factors for LSD seropositivity. The overall animal and herd-level seroprevalences were 8.7% (95% CI: 7.0–9.3) and 72.3% (95% CI: 70.0–80.3), respectively. Animal-level seroprevalence in Central region (OR = 2.13, p = 0.05, 95% CI: 1.10–4.64) was significantly different from the Northern region (Reference) and Western region (OR = 0.84, p = 0.66, 95% CI: 0.39–1.81). Management type, sex, age, mean annual precipitation > 1000 mm, and drinking from communal water sources were statistically significant risk factors for occurrence of anti-LSDV antibodies in cattle. Breed, region, herd size, contact with buffalo and other wildlife and introduction of new cattle did not have a statistically significant association with being positive for LSDV.

Conclusion

We report a high herd-level LSDV seroprevalence in Uganda with a moderate animal-level seroprevalence. Cattle with the highest risk of LSD infection in Uganda are those in fenced farms, females > 25 months old, in an area with a mean annual rainfall > 1000 mm, and drinking from a communal water source.

Background

Lumpy skin disease (LSD) is a transboundary disease of cattle. The etiological agent of LSD is a double stranded DNA Capripoxvirus which belongs to the family Poxviridae [1, 2]. This disease is defined by mild to severe symptoms which include fever and development of large nodular skin and internal organ lesions [3,4,5,6]. These symptoms lead to death in 1–5% of the cases [7]. Lumpy skin disease virus (LSDV) is closely related to two other viruses in the genus Capripoxvirus, sheeppox and goatpox viruses [5]. Transmission of LSDV is primarily by mechanical means, by several probable arthropod vectors such as biting flies, mosquitoes (Aedes aegypti) [8] and three tick species of the family Ixodidae, namely Rhipicephalus appendiculatus, Rhipicephalus decoloratus and Amblyomma hebraeum) [9]. These vectors have been shown to transmit LSDV under experimental conditions, however their capacity to transmit disease under natural field conditions is still unknown. Stomoxys calcitrans (Stable fly) has been reported as the most probable vector for LSDV due to its abundance and being associated with outbreaks [10, 11]. Veterinary equipment, specifically needles [5, 12] have also been reported to transmit the virus. The possible vectors of LSDV (mosquitoes, flies, ticks) are all present in Uganda and are highly likely to be responsible for disease spread, although the contribution of different vectors in LSDV transmission has not yet been studied in the country.

Morbidity of LSD varies greatly and ranges from 3 to 85% in different epizootic situations. In endemic areas, morbidity is estimated at 10% [5]. Mortality due to LSD varies between 1 and 3%, but up to 40% have been reported in severe outbreak situations [7]. These broad ranges for morbidity and mortality are likely to be due to variation in cattle breed, health status, viral isolates and insect vectors involved in the transmission [4, 13]. For instance in Africa, imported breeds from Europe or Australia have shown high susceptibility to LSD [13,14,15].

Control and prevention of LSD is undertaken through vaccination, quarantines, livestock movement controls, vector control, slaughter of infected and exposed animals and cleaning and disinfection of the premises [5]. Vaccination is reported to be the most effective method for controlling LSD in both disease endemic and non-endemic areas [16]. At present, only live vaccines are commercially available against LSDV, with different vaccines licensed for use in different countries although the most common LSDV strain used in attenuated vaccines is the Neethling strain. This strain was reported to be highly effective in controlling epidemics in the Balkans [17]. In countries where goat pox is present, attenuated goat pox virus strain can be used, like the Gorgan goat pox strain. In Uganda, two Neethling virus based vaccines, BOVIVAX LSD-N and LUMPYVAX™ are licensed for use in the country [18]. Vaccination against LSD is primarily done by commercial farmers who can afford the costs of vaccination while small holder farmers largely do not vaccinate against LSD.

Lumpy skin disease was first reported in northern Rhodesia (Zambia) in 1929 [19] and the disease remained endemic to sub-Saharan Africa until 1990, when it extended into North Africa and then into the Middle East [20, 21]. More recently, LSD has spread into parts of southeast Europe, with outbreaks reported in Turkey and Russia amongst other countries [22,23,24,25,26]. This disease therefore has the potential for global emergence [27]. In Uganda, there is no published literature about when LSD was first identified. The disease is thought to have spread from southern Africa into Uganda between 1955 and 1960 [28]. The disease (LSD) is currently present in all geographical regions of the country, with several outbreaks reported annually. Suspected outbreaks are reported based on clinical signs and are confirmed by the National Animal Disease Diagnostics and Epidemiology Centre (NADDEC) Laboratories, using polymerase chain reaction (PCR)-based methods [29]. Following LSDV confirmation, control is mainly by isolation of infected animals from the herd and treatment of secondary infections with injectable antibiotics and non-steroidal anti-inflammatories (NSAIDs). Occasionally, vaccination of animals is carried out in the affected herds and in neighboring herds to prevent further spread of disease. These vaccinations are usually self-funded by the farmers and are therefore based on availability of vaccines, interest in pursuing vaccination and on financial ability of farmers. This therefore limits the number of animals that get vaccinated. Vaccination against LSD is mainly done by commercial farmers with large herds while small holder farmers, which constitute the vast majority of livestock holders, do not vaccinate against LSD.

A number of methods have been used for serological investigation of LSDV. These tests include a skin hypersensitivity test [3], virus neutralization test (VNT), immunoperoxidase monolayer assay (IPMA) [30] or indirect fluorescent antibody test (IFAT) [31] and ELISA. The antibody ELISAs developed in the past have faced challenges like difficulty in obtaining sufficient quantities of heat inactivated antigen and instability of recombinant antigens [32, 33]. This had therefore led to the inability to do mass screening of LSD using a reliable method. This study utilizes the first commercially available ELISA for detection of LSD antibodies in naturally infected and in vaccinated animals. This ELISA, ID Screen® Capripox double antigen multi-species ELISA, is able to detect antibodies against Capripoxviruses including lumpy skin disease virus (LSDV), sheeppox virus and goatpox virus in serum and plasma. It has demonstrated very high specificity (> 99.7%) and does not cross-react with parapox viruses. It also has equivalent sensitivity to immunoperoxidase monolayer assay (IPMA) [34], when compared to VNT and IFAT respectively. This ELISA is easy to perform and allows for high throughput screening without requiring high-level containment facilities [35].

In Uganda livestock farming contributes 1.7–3.2% of GDP [36], however growth in this sector has been slow because of livestock diseases. LSD is one of the many important cattle diseases in Uganda, but unlike other cattle diseases in the country, little is known about the epidemiology of the disease and as a result there is presently no control strategy. LSD is usually reported by farmers and district authorities and is enzootic in all regions of the country. In order to understand more about the epidemiology of LSD in Uganda, a recent retrospective study assessed the spatiotemporal distribution of reported LSD outbreaks [37]. This study therefore seeks to provide more epidemiological information about LSD in Uganda by estimating the herd- and animal-level seroprevalence, and risk factors for seropositivity, in selected herds with no history of vaccination against LSD, within all four major geographical regions of Uganda. This will help in adding to the scarce epidemiological knowledge of LSD in Uganda and potentially contribute to better control measures for the disease.

Results

Demographic characteristics of the study population

Blood samples collected from 2,263 cattle in 21 districts of Uganda between July 2016 and August 2017 were screened for presence of antibodies against LSDV. The average number of cattle sampled per region was 565.8 while the mean number sampled per herd was 28.6, distributed over 65 herds. Of the cattle sampled, 1,840 were female while 423 were male. Most of the cattle sampled were of the zebu breed (1,094), followed by Ankole breed (834), Friesian (146), Boran (129) and Friesian-Ankole crossbreeds (60).

Seroprevalence of LSD antibodies at animal level in Uganda

The overall animal-level seroprevalence of lumpy skin disease in Uganda was found to be 8.7% (95% CI: 7.1–9.4). The highest regional seroprevalence was 12.8% (95% CI: 9.3–15.0) in the Central region, followed by 10.3% (95% CI: 7.3–12.4) in the Eastern region, 6.1% (95% CI: 4.0–8.1) in the Northern region, and 6.2% (95% CI: 4.2–8.0) in Western region respectively. The differences in animal level prevalence amongst these four regions were found to be statistically significant, with there being a statistically significant difference in seroprevalence between the Central region (OR = 2.13, p = 0.05, 95% CI: 1.10–4.64) as compared to the Northern region.

Herd-level prevalence

Among the 65 herds investigated in this study, 47 (72.3%) of the herds had at least one seropositive animal for LSDV. Herd-level seroprevalence at the regional level was 100% for the herds sampled in Central and Eastern Uganda, while the north and west had herd-level prevalences of 69.3 and 59.4%, respectively. Within-herd seroprevalence varied between 0 and 35.6%, with an average within herd seroprevalence of 7.7%. Prevalence per sampled herd and at regional level are summarised in Table 1 and Additional file 3.

Table 1 Animal- and herd-level seroprevalence of lumpy skin disease in the four major geographical regions of Uganda
Full size table

Risk factors for LSDV seropositivity

Univariable mixed effect logistic regression was performed on the following possible risk factors for LSD seropositivity: Age, management type, sex, breed, mean annual rainfall, region, contact with buffalo, communal water source, new cattle introduced, contact with other wildlife and herd size. Out of the eleven possible risk factors analysed, management type, age, sex, mean annual rainfall, contact with buffalo and communal water sources, and with p < 0.2 were selected for multivariable analysis. The best fit model included management type, sex, age, mean annual rainfall, contact with buffalo, and communal water sources as significant factors associated with LSDV seropositivity. As compared to pastoral and communally grazed herds, fenced farms were significantly associated with seropositivity (OR = 5.26; 95%CI: 2.64–10.48, p < 0.01). In addition, higher mean annual rainfall (1001-1200 mm-OR = 5.60; 95%CI: 2.35–13.34, p < 0.01; 1201-1400 mm-OR = 4.58; 95%CI: 2.23–9.40, P < 0.01), female cattle (OR = 1.72; 95%CI: 1.02–2.92, p = 0.04), age > 25 months (OR = 1.96; 95%CI: 1.15–3.34), and drinking from communal water sources (OR = 3.31; 95%CI: 1.42–7.71, p = 0.01) were significant factors associated with LSDV seropositivity (Table 2). Daily reported contact with buffalo (OR = 1.78; 95%CI: 0.50–6.31, p = 0.37) was found not to be a significant factor for LSDV seropositivity, whereas weekly or monthly contact with buffalo had a protective effect, as shown in Table 2.

Table 2 Best-fit multivariable model for animal-level risk factors associated with LSDV sero-positivity using mixed effect logistic regression modelling with herd as random effect
Full size table

Discussion

In this study we investigated the seroprevalence and risk factors for seropositivity against lumpy skin disease virus in the four major geographical regions of Uganda using the first commercially available antibody ELISA test for LSDV. This is the first study reporting seroprevalence of LSDV in cattle in Uganda. We found an overall animal-level seroprevalence of 8.7% and an overall herd-level seroprevalence of 72.3%.

The overall animal-level sero-prevalence of 8.7% in Uganda is comparable to LSDV prevalences reported by previous studies in the East African region. In Ethiopia, two studies have reported a lower prevalence; one study by Abera et al reported a sero-prevalence of 6.43% [15] while the other study by Hailu et al reported prevalence of clinical LSD at 7.4% [38] in north-eastern Ethiopia. Higher animal-level prevalences have also been reported by Gari et al [39], who estimated a sero-prevalence of 23–31% in different agroecological zones in Ethiopia, and Molla et al [40] who reported a sero-prevalence of 26.5%. Comparison of herd-level sero-prevalence, however, showed a higher prevalence in Uganda (72.3%) than herd level sero-prevalence reported in Ethiopia. Previous studies have reported varying herd-level prevalences in lowland (50%), midland (26%) and highland agro-climate zones (64%) in Ethiopia [39]. Herd-level prevalence was reported as 52.6% in central and northwestern Ethiopia [40] and 5.95% in western Ethiopia [15]. There have been no recent studies on sero-prevalence of LSDV in Uganda’s neighboring countries of Kenya, South Sudan, Congo DRC, Tanzania and Rwanda. This may be mainly be due the fact that the previously available tests for serodiagnosis of LSDV required virus isolation and high levels of biocontainment, which are mostly lacking in these countries. Serum neutralization tests (SNT), immune peroxidase monolayer assays, and indirect fluorescent antibody tests are accurate but have limitations for screening large numbers of serum samples. In addition, many ELISAs developed in the past have not been made commercially available [35].

When we compared animal-level sero-prevalence amongst the four regions of Uganda, the highest sero-prevalence was reported in the Central region (12.8%), followed by 10.3% in Eastern region, 6.2% in Western region, and 6.1% in the Northern region. These differences in animal-level sero-prevalence amongst these four regions were found to be statistically significant, with significantly higher sero-prevalences in the Central region as compared to the Northern region. There was no significant difference between sero-prevalence in the Central and East. These findings suggest that cattle in Central and Eastern Uganda are exposed to LSDV at higher rates than in the West and Northern regions. This could be due to environmental conditions in these two regions being favorable for reproduction of biting arthropods which act as vectors for LSDV and due to differences in husbandry practices. These regional differences in sero-prevalence of LSDV are in agreement with our previous findings which, using retrospective reporting data, demonstrated the highest numbers of clinical cases of LSD in Uganda to be in the Central and Eastern regions [37]. Other than the risk factors investigated in this study, there could be a number of bioclimatic and epidemiological variables responsible for these high prevalences that warrant further investigation. For example, increased unregulated acaricide use and resistance in Uganda may also be playing a role in maintaining high LSD prevalence, since ticks are known to transmit LSD [41].

Across Uganda, 72.3% of herds reported at least one seropositive animal for LSDV. However, all herds tested in Central and Eastern Uganda had at least one positive animal per herd, thus giving a herd-level prevalence of 100%, while the North and West had lower herd-level prevalences of 69.3 and 59.4%, respectively. It is reported that the duration of antibodies in infected cattle is short-lived and declines within 6 months following infection [42, 43]. This high herd-level prevalence, particularly in Central and Eastern Uganda, suggests that the LSDV incidence is frequent and that the virus may be maintained locally within cattle populations.

We additionally studied risk factors for seropositivity for LSDV, and found management type, sex, age, mean annual rainfall as significant factors associated with LSDV in Uganda. Cattle kept in fenced farms (OR = 5.26: 95%CI: 2.64–10.48) showed higher risk for LSD infection than those grazed communally or in a pastoral husbandry system. In fenced farms, cattle are kept in a confined grazing area, potentially allowing for biting flies to easily transmit disease. Higher intensity of range use within fenced farms may also increase transmission of environmentally-transmitted pathogens [44]. Alternatively, fenced farms may be a management system that is common in wetter environments, and thus the significance of fenced farms may be an artifact underlying environmental conditions that are conducive to both higher densities of arthropod vectors as well as fenced farming practices. We also found an association between being female and seropositivity; female animals were almost twice more likely to be seropositive when compared to males. In this study, adult cattle > 25 months were found to have higher odds of seropositivity (OR = 1.96) as compared to young cattle (0–12 months). The reason for higher seropositivity in older animals may be related to duration of exposure, which increases their chance of infection. Similarly, female animals are usually kept longer by farmers while males are sold off at a younger age, thus the effect of sex may be an artifact of duration of exposure. These findings agree with Molla et al [40] (OR = 2.44) and Abera et al [15] (OR = 3.41), both of which recorded higher odds of LSDV in adults compared to calves. This may also be due to low frequency of exposure, because calves are kept at home in small enclosed spaces away from biting insects. In a mathematical modeling study evaluating different routes of LSDV transmission, Magori-Cohen et al [45] reported that suckling calves showed the lowest infection rate, possibly due to their location away from infected adult cattle and biting flies.

Mean annual rainfall ranges of 1001-1200 mm (OR = 5.60: 95%CI: 2.35–13.34) and 1201-1400 mm (OR = 4.58: 95%CI: 2.23–9.40) were found to be associated with LSDV seropositivity as compared to mean annual rainfall less than 1000 mm. High rainfall is associated with increased arthropod density, therefore increasing populations of insect vectors responsible for mechanical transmission of LSDV. Here, we additionally report drinking from communal water sources as a risk factor for LSDV seropositivity. Cattle drinking from a communal water source were three times more likely to be seropositive than those drinking from a non-communal water source. This is in agreement with other studies reporting that animals having frequent contact with other animals at communal grazing and watering points are more at risk to acquire LSDV [38, 46]. We found weekly/monthly contact with buffalo to be protective against seropositivity, while daily contact with buffalo did not have a significant association perhaps due to a small numbers of herds within this latter category. These findings are likely reflective of some unmeasured variable or factor that was not fully captured in this study, such as finer scale environmental gradients in which contact with wildlife served as a proxy for drier conditions .

In this study we compared local Ankole, Boran and Zebu cattle breeds with Friesian and found no association between cattle breed and LSDV seropositivity. This is unlike other studies, by Davies FG [13] and Abera et al [15] who reported Channel Island breeds and Zebu-Friesian cross breeds respectively, as having a higher risk for LSD as compared to local breeds. We also found no association between herd size and introduction (re-stocking) of new cattle to the herds and increased LSDV seropositivity.

Conclusion

This is the first study on sero-prevalence of LSDV in Uganda and it provides baseline information on the occurrence of LSDV in Uganda. This study reported a high herd-level sero-prevalence of LSDV in Uganda, demonstrating that LSDV is an important disease in Uganda. The overall animal-level sero-prevalence is moderate. This study also confirms that LSDV is prevalent in all regions of the country, with higher rates of exposure in the Central and Eastern regions. Cattle with the highest risk of LSDV sero-positivity were found in an area with a mean annual rainfall > 1001 mm, those in fenced farms, females, cattle older than 25 months, and drinking from a communal water source. Appropriate control measures should be developed with our findings in mind.

Methods

Description of study area

Uganda is an East African country found between latitudes 4°N and 2°S, and longitudes 29° and 35°E, with an area of about 241,038 km2. Uganda averages about 3,609 ft. (1,100 m) above sea level, and a large portion of its southern border is lakeshore. The country is mostly plateau with some undulating hills and low mountains. Uganda is divided into four administrative regions: North, East, Central and West, comprising 121 districts. The districts are further divided into counties, sub-counties, parishes and villages. The cattle population in Uganda is estimated to be about 11.4 million heads of which 34.2% are in the north, 21.8% in the East, 21.7% in Central and 22.3% in the west [47]. Within these regions the highest number of cattle are found in districts along the Uganda cattle corridor, which is an area stretching diagonally across the country from the southwest to the northeast. This cross sectional study was carried out in 21 districts of Uganda spread-out in all four regions in Uganda, in herds with no history of LSD vaccination (Fig. 1). These selected areas are comprised of two major livestock farming systems: mixed rainfed crop-livestock systems and livestock-only farming systems. In the mixed rainfed crop-livestock system, crops and livestock farming are practiced together, whereas in the livestock-only, rangeland-based livestock production system, livestock farming is the major type of farming with nearly no crop farming practiced. The livestock-only rangelands are part of the Uganda cattle corridor.

Fig. 1
figure1

Map of Uganda showing the study districts in yellow and gps coordinates (red dots) of sites where individual cattle herds were sampled (Source of map: This study)

Full size image

Study design, sample size determination, and data collection

The first aim was to estimate differences in sero-prevalence across the four regions of Uganda, as the four regions have varying mean annual rainfall and livestock production systems [48]. Target sample size per region was 520, which was based on the sample size needed to detect differences between two proportions with 0.8 power and 0.95 confidence level. We assumed that sero-prevalences in Uganda would fall between estimates from elsewhere in Eastern Africa: 8% [15, 31] and 16% [39]. The sampling frame included the 211 herds that were sampled as part of a nationwide sero-survey for foot-and-mouth disease virus from 2016 to 2017 (Additional file 1). During this sero-survey, information on vaccination against common cattle disease was collected and herds with no history of LSD vaccination were selected for this study. As suggested by Dohoo et al. (2009) for study designs with multistage sampling, herds within each region were selected such that the probability that each herd was selected was proportional to their herd size [49]. Only herds with at least 20 animals were included. Based on these criteria, 2,263 samples from 65 different herds were screened for LSDV. Livestock in this study were indigenous short horned zebu, Ankole, Boran, Friesian and crossbred cattle of all age groups ranging between 2 months to 6 years old. In the course of sample collection, cattle owners were consulted to help estimate the age of each sampled animal. All the sampled cattle were grouped into three age based categories; cattle between 0 and 12 months were considered calves, cattle of 13–24 months were considered young, and cattle older than 24 months were considered adults. At each sampling location, a questionnaire was administered to the animal owner to collect information about possible risk factors at the animal and herd-level. Assistance in administering the questionnaire was provided by area (local) veterinary personnel in the appropriate language/dialect. The GPS of the herd was recorded.

Sample collection and handling

Full disposable 8.5 ml sterile Vacutainer SST tubes of whole blood samples were collected from the jugular vein of each animal. The tubes were then kept protected from direct sun light at room temperature until the blood clotted and sera were separated by centrifugation at 3000 rpm for 10 min. The separated sera were transferred to sterile 2 ml cryovials, labeled with animal number, age, sex and district name. The samples were then transported to Makerere University, College Of Veterinary Medicine Animal Resources and Biosecurity (COVAB) molecular biology laboratory for serological examination using an indirect ELISA test.

ELISA test for LSD antibodies

Antibodies against LSDV were detected using a Double Antigen ELISA (ID Screen®) for the detection of antibodies against Capripoxviruses. Briefly, to perform the ELISA test, 50 μL of each test serum sample was diluted in 50 μL of Dilution buffer 19 and added to an ELISA plate coated with Capripox virus purified antigen. Positive and negative control sera were also similarly diluted and added to the same ELISA plate. The ELISA plate was incubated for 90 min at 21 °C, wells were emptied, then washed 5 times with wash solution before adding 100 μL conjugate to each well, followed by incubation for 30 min. Wells were then emptied and washed 5 times, then 100 μL of substrate solution was added to each well and the plate covered and incubated for 15 min. 100 μL stop solution was then added and the optical density (OD) read at 450 nm using a microplate reader (Biochrom Asys UVM 340, UK). For each sample, the percentage OD of sample/ OD of positive control (S/P percentage) was calculated using the formula:

$$ S/P\%=\frac{OD_{sample}-{OD}_{Nc}\ }{OD_{PC}-{OD}_{NC}}\times 100 $$

Where OD sample is the optical density of sample, ODPC is optical density of positive control, and ODNC is optical the optical density of negative control. Samples presenting an S/P% less than 30% were considered negative while those with S/P% greater than or equal to 30% were considered positive.

Data management and statistical analysis

Apparent animal-level seroprevalence was calculated by dividing the number of LSDV positive animals by the total number of animals tested while herd-level prevalence was determined by dividing positive herds by total number of herds. A herd would be considered positive if at least one animal tested seropositive for lumpy skin disease. To calculate true seroprevalence, the apparent seroprevalence (AP) was adjusted for sensitivity (Se) and specificity (Sp) of ELISA test (91% and 99.7%, respectively). True prevalence was used to report seroprevalence at the animal-level for within-herd, regional, and national seroprevalences. True prevalence was calculated using the formula by Stevenson 2007 [50]:

$$ True\ prevalence=\frac{AP+ Sp-1}{Se+ Sp-1} $$

Although we do not anticipate a seasonal trend for serological data, we evaluated potential seasonality by plotting within-herd seroprevalence by month (Additional file 2). Possible risk factors for seropositivity were selected using univariable mixed effect logistic regression analysis with herd ID as a random effect to account for clustering at herd level, and all variables that were significant in the univariable analysis (p < 0.2) were further checked for co-linearity before multivariable analysis. During multivariable mixed effect logistic regression analysis, all non-significant variables were removed sequentially by backward elimination where the model with the lowest Akaike Information Criterion (AIC) value was chosen as the best model. At every step during model development, confounding was assessed by checking for changes in parameter estimates, and changes > 25% were considered to indicate confounding. To compare differences in animal level prevalence in the four regions of Uganda we performed a logistic regression with region as a categorical variable and herd as a random effect. In all the analyses performed, confidence levels were calculated at 95%, and a P value < 0.05 was used for statistical significance level, except for univariable analysis. Data analysis was done using STATA 2010, version 16 software.

Availability of data and materials

The datasets used and/or analysed during the current study are available from the corresponding author on reasonable request.

Abbreviations

COVAB:

College of Veterinary Medicine Animal Resources and Biosecurity

LSD:

Lumpy Skin Disease

LSD:

Lumpy Skin Disease Virus

MAAIF:

Ministry of Agriculture Animal Industry and Fisheries

References

  1. 1.

    Woods JA. Lumpy skin disease-A review. Trop Anim Health Prod. 1988;20(1):11–7.

    CAS  Article  Google Scholar 

  2. 2.

    Davies FG. Observations on the epidemiology of lumpy skin disease in Kenya. J Hyg (Lond). 1982;88(1):95–102.

    CAS  Article  Google Scholar 

  3. 3.

    Capstick PB, Coakley W. Lumpy skin disease. The determination of the immune status of cattle by an intra-dermal test. Res Vet Sci. 1962;3:287–91.

    Article  Google Scholar 

  4. 4.

    Babiuk S, Bowden TR, Parkyn G, Dalman B, Manning L, Neufeld J, et al. Quantification of lumpy skin disease virus following experimental infection in cattle. Transbound Emerg Dis. 2008;55(7):299–307.

    CAS  Article  Google Scholar 

  5. 5.

    OIE Terrestrial Manual. Aetiology Epidemiology Diagnosis Prevention and Control References Oie. 2012:1–5.World Organisation for Animal Health (OIE). Lumpy Skin Disease: Aetiology Epidemiology, Diagnosis, Prevention and Control References. Paris: Organization International des Epizootics; 2012. http://www.oie.int/fileadmin/Home/eng/Animal_Health_in_the_World/docs/pdf/Disease_cards/LUMPY_SKIN_DISEASE_FINAL.pdf.

  6. 6.

    Abutarbush SM, Ababneh MM, Al Zoubi IG, Al Sheyab OM, Al Zoubi MG, Alekish MO, et al. Lumpy skin disease in Jordan: disease emergence, clinical signs, complications and preliminary-associated economic losses. Transbound Emerg Dis. 2015;62(5):549–54.

    CAS  Article  Google Scholar 

  7. 7.

    Coetzer JAW. Lumpy skin disease, in: Infectious diseases of livestock, edited by Coetzer JAW & Tustin RC. Cape Town: Oxford University Press Southern Africa; 2004;2:1268-1276

  8. 8.

    Chihota CM, Rennie LF, Kitching RP, Mellor PS. Mechanical transmission of lumpy skin disease virus by Aedes aegypti (Diptera: Culicidae). Epidemiol Infect. 2001. https://doi.org/10.1017/S0950268801005179

    CAS  Article  Google Scholar 

  9. 9.

    Lubinga JC, Clift SJ, Tuppurainen ESM, Stoltsz WH, Babiuk S, Coetzer JAW, et al. Demonstration of lumpy skin disease virus infection in Amblyomma hebraeum and Rhipicephalus appendiculatus ticks using immunohistochemistry. Ticks Tick Borne Dis [Internet]. 2014 Mar 1 [cited 2019 May 7];5(2):113–120. Available from: https://www.sciencedirect.com/science/article/abs/pii/S1877959X13001015?via%3Dihub.

  10. 10.

    Yeruham I, Nir O, Braverman Y, Davidson M, Grinstein H, Haymovitch M, et al. Spread of lumpy skin disease in Israeli dairy herds. Vet Rec. 1995;137(4):91–3.

    CAS  Article  Google Scholar 

  11. 11.

    Kahana-Sutin E, Klement E, Lensky I, Gottlieb Y. High relative abundance of the stable fly Stomoxys calcitrans is associated with lumpy skin disease outbreaks in Israeli dairy farms. Med Vet Entomol. 2017;31(2):150–60.

    CAS  Article  Google Scholar 

  12. 12.

    Carn VM, Kitching RP. An investigation of possible routes of transmission of lumpy skin disease virus (Neethling). Epidemiol Infect [Internet]. 1995;114(1):219–26 Available from: http://www.pubmedcentral.nih.gov/articlerender.fcgi?artid=2271331&tool=pmcentrez&rendertype=abstract.

    CAS  Article  Google Scholar 

  13. 13.

    Davies FG. Lumpy skin disease of cattle: a growing problem in Africa and the near east. World Anim Rev [Internet]. 1991;68:37–42 Available from: http://www.fao.org/ag/aGa/agap/frg/feedback/war/u4900b/u4900b0d.htm.

    Google Scholar 

  14. 14.

    Gari G, Bonnet P, Roger F, Waret-Szkuta A. Epidemiological aspects and financial impact of lumpy skin disease in Ethiopia. Prev Vet Med. 2011;102(4):274–83.

    CAS  Article  Google Scholar 

  15. 15.

    Abera Z, Degefu H, Gari G, Kidane M. Sero-prevalence of lumpy skin disease in selected districts of west Wollega zone. BMC Vet Res [Internet]. 2015:1–9. Available from. https://doi.org/10.1186/s12917-015-0432-7.

  16. 16.

    European Food Safety Authority. Lumpy skin disease: vaccination is most effective control method [internet]. [cited 2019 may 7]. Available from: https://www.efsa.europa.eu/en/press/news/160809.

  17. 17.

    Klement E, Broglia A, Antoniou SE, Tsiamadis V, Plevraki E, Petrović T, et al. Neethling vaccine proved highly effective in controlling lumpy skin disease epidemics in the Balkans. Prev Vet Med. 2018;(August.

  18. 18.

    Hovari M, Beltran-Alcrudo D. Guide to develop a lumpy skin disease emergency vaccination plan; 2018. http://www.fao.org/fileadmin/user_upload/reu/europe/documents/LSDVG.pdf.

  19. 19.

    MacDonald RAS. Pseudo-urticaria of cattle. Northern Rhodesian Department of Animal Health, Annual Report 1930, 20–21.

  20. 20.

    Ali AA, Esmat M, Attia H, Selim A, Abdel-Hamid YM. Clinical and pathological studies of lumpy skin disease in Egypt. Vet Rec. 1990;127(22):549–50.

    CAS  PubMed  Google Scholar 

  21. 21.

    Fagbo S, Coetzer JAW, Venter EH. Seroprevalence of Rift Valley fever and lumpy skin disease in African buffalo (&lt;i&gt;Syncerus caffer&lt;/i&gt;) in the Kruger National Park and Hluhluwe-iMfolozi Park, South Africa. J S Afr Vet Assoc [Internet]. 2014;85(1):1–8 Available from: http://www.jsava.co.za/index.php/jsava/article/view/1075.

    Google Scholar 

  22. 22.

    Standing Group of Experts on Lumpy Skin Disease in the South East Europe region under the GF-TADs umbrella, Fifth meeting (SGE LSD5). Lumpy skin disease ( LSD ) epidemiological situation in Europe. 2017. https://web.oie.int/RR-Europe/eng/Regprog/docs/docsLSD5/SGE%20LSD5%20(Budva,%20OCt2017)%20-%20Epidemiological%20situation%20in%20Europe%20(DD).pdf.

  23. 23.

    Şevik M, Doğan M. Epidemiological and molecular studies on lumpy skin disease outbreaks in Turkey during 2014–2015. Transbound Emerg Dis. 2017;64(4):1268–79.

    Article  Google Scholar 

  24. 24.

    The Russian Federation LSD report Dr Artem Metlin. 2016;(September).

  25. 25.

    Albayrak H, Ozan E, Kadi H, Cavunt A, Tamer C, Tutuncu M. Molecular detection and seasonal distribution of lumpy skin disease virus in cattle breeds in Turkey. 2018;74(3):175–178.

  26. 26.

    European Food Safety Authority (EFSA). Lumpy skin disease: data collection and analysis [internet], vol. 15. EFSA Journal. 2017. Available from: http://doi.wiley.com/10.2903/j.efsa.2017.4773

  27. 27.

    Tuppurainen ESM, Oura CAL. Review: lumpy skin disease: an emerging threat to Europe, the Middle East and Asia. Transbound Emerg Dis. 2012;59(1):40–8.

    CAS  Article  Google Scholar 

  28. 28.

    Nawathe, Paden J, Confl R. In Nigeria. Pieleg Polozna. 1982;36(3):19, 25

  29. 29.

    World Organisation for Animal Health (OIE). Lumpy Skin Disease. In: OIE Terrestrial Manual [Internet]. 2017. p. 56. Available from: https://www.bertelsmann-stiftung.de/fileadmin/files/BSt/Publikationen/GrauePublikationen/MT_Globalization_Report_2018.pdf%0A, http://eprints.lse.ac.uk/43447/1/India_globalisation%2Csocietyandinequalities%28lsero%29.pdf%0A, https://www.quora.com/What-is-the.

  30. 30.

    Haegeman A, Zro K, Sammin D, Vandenbussche F, Ennaji MM, De Clercq K. Investigation of a possible link between vaccination and the 2010 sheep pox epizootic in Morocco. Transbound Emerg Dis. 2016;63(6):e278–87.

    CAS  Article  Google Scholar 

  31. 31.

    Gari G, Biteau-Coroller F, LeGoff C, Caufour P, Roger F. Evaluation of indirect fluorescent antibody test (IFAT) for the diagnosis and screening of lumpy skin disease using Bayesian method. Vet Microbiol. 2008;129(3–4):269–80.

    CAS  Article  Google Scholar 

  32. 32.

    Bowden TR, Coupar BE, Babiuk SL, White JR, Boyd V, Duch CJ, et al. Detection of antibodies specific for sheeppox and goatpox viruses using recombinant capripoxvirus antigens in an indirect enzyme-linked immunosorbent assay. J Virol Methods. 2009;161(1):19–29.

    CAS  Article  Google Scholar 

  33. 33.

    Babiuk S, Wallace DB, Smith SJ, Bowden TR, Dalman B, Parkyn G, et al. Detection of antibodies against capripoxviruses using an inactivated sheeppox virus ELISA. Transbound Emerg Dis. 2009;56(4):132–41.

    CAS  Article  Google Scholar 

  34. 34.

    IDvet 34790 Grabels F. ID Screen® Capripox Double Antigen Multi-species [Internet]. 2018. Available from: https://www.id-vet.com/produit/id-screen-capripox-double-antigen-multi-species/

  35. 35.

    Tuppurainen E. Diagnostic assays for the detection of lumpy skin disease virus and antibodies. 2017;(October).

  36. 36.

    Behnke R, Nakirya M. The contribution of livestock to the Ugandan economy. IGAD Livest Policy Initiat Work Pap [Internet]. 2012;(02):1–37 Available from: http://citeseerx.ist.psu.edu/viewdoc/download?doi=10.1.1.366.4644&rep=rep1&type=pdf.

  37. 37.

    Ochwo S, Vanderwaal K, Munsey A, Ndekezi C, Mwebe R, Rose A, et al. Spatial and temporal distribution of lumpy skin disease outbreaks in Uganda ( 2002–2016 ). 2018;1–12.

  38. 38.

    Hailu B, Tolosa T, Gari G. Estimated prevalence and risk factors associated with clinical lumpy skin disease in North-Eastern Ethiopia. Prev Vet Med [Internet]. 2014;115(1–2):64–68. Available from: https://doi.org/10.1016/j.prevetmed.2014.03.013

    Article  Google Scholar 

  39. 39.

    Gari G, Grosbois V, Waret-szkuta A, Babiuk S, Jacquiet P, Roger F. Lumpy skin disease in Ethiopia : Seroprevalence study across different agro-climate zones. Acta Trop [Internet]. 2012;123(2):101–106. Available from: https://doi.org/10.1016/j.actatropica.2012.04.009

    CAS  Article  Google Scholar 

  40. 40.

    Molla W, Frankena K, Gari G, Kidane M, Shegu D, Jong MCM De. Seroprevalence and risk factors of lumpy skin disease in Ethiopia. Prev Vet Med [Internet] 2018; Available from: https://doi.org/10.1016/j.prevetmed.2018.09.029.

    Article  Google Scholar 

  41. 41.

    Vudriko P, Okwee-acai J, Tayebwa DS, Byaruhanga J, Kakooza S, Wampande E, et al. Emergence of multi-acaricide resistant Rhipicephalus ticks and its implication on chemical tick control in Uganda. Parasit Vectors. 2016.

  42. 42.

    Tuppurainen ESM, Babiuk S, Klement E. Lumpy Skin Disease, 2018. Springer International Publishing, pages 47-51. https://doi.org/10.1007/978-3-319-92411-3.

    Google Scholar 

  43. 43.

    Weiss KE. Lumpy Skin Disease Virus. In: Cytomegaloviruses Rinderpest Virus Lumpy Skin Disease Virus Virology Monographs (Die Virusforschung in Einzeldarstellungen). Springer, Berlin, Heidelberg; 1968. p. 111–131.

    Google Scholar 

  44. 44.

    Ezenwa VO. Parasite infection rates of impala (Aepyceros melampus) in fenced game reserves in relation to reserve characteristics. Biol Conserv. 2004;118(3):397–401.

    Article  Google Scholar 

  45. 45.

    Magori-Cohen R, Louzoun Y, Herziger Y, Oron E, Arazi A, Tuppurainen E, et al. Mathematical modelling and evaluation of the different routes of transmission of lumpy skin disease virus. Vet Res. 2012;43(1):1–13.

    Article  Google Scholar 

  46. 46.

    Gari G, Waret-Szkuta A, Grosbois V, Jacquiet P, Roger FR. Risk factors associated with observed clinical lumpy skin disease in Ethiopia. Epidemiol Infect. 2010:1657–66.

    CAS  Article  Google Scholar 

  47. 47.

    Ministry Of Agriculture Animal Industry and Fisheries, Uganda. The National Livestock Census a Summary Report of the National Livestock Census, 2008. 2008

  48. 48.

    FAO and USAID. ASL2050 Livestock production systems spotlight - Uganda [Internet]. 2017. Available from: http://www.fao.org/3/i8713en/I8713EN.pdf.

  49. 49.

    Ian Dohoo, Wayne Martin, Henrik Stryhn. Veterinary epidemiologic research. 2nd edition. Charlottetown, Canada: VER Inc; 2009:865.

  50. 50.

    Stevenson M. An Introduction to Veterinary Epidemiology. Biometrics. Palmerston North: EpiCentre, IVABS; 2007. p. 1–92.

Download references

Acknowledgements

The authors would like to acknowledge the district veterinary and local government staff who helped us during field sample collection. We would also like to acknowledge the different cattle farmers who agreed to participate in this study.

Funding

This research was funded by the University Of Minnesota Academic Health Center and they had no role in the design and execution of the study as well as the decision to publish this manuscript.

Author information

Affiliations

  1. College of Veterinary Medicine, Animal resources and Biosecurity, Makerere University, P.O.BOX 7062, Kampala, Uganda

    Sylvester Ochwo, Joseph Nkamwesiga, Christian Ndekezi & Frank N. Mwiine

  2. College of Veterinary Medicine, University of Minnesota, 1365 Gortner Avenue, St. Paul, MN, MN 55108, USA

    Kimberly VanderWaal & Anna Munsey

  3. College of Natural Sciences, Makerere University, P.O.BOX 7062, Kampala, Uganda

    Elda Auma

Authors
  1. Sylvester Ochwo
    View author publications

    You can also search for this author in PubMed Google Scholar

  2. Kimberly VanderWaal
    View author publications

    You can also search for this author in PubMed Google Scholar

  3. Anna Munsey
    View author publications

    You can also search for this author in PubMed Google Scholar

  4. Joseph Nkamwesiga
    View author publications

    You can also search for this author in PubMed Google Scholar

  5. Christian Ndekezi
    View author publications

    You can also search for this author in PubMed Google Scholar

  6. Elda Auma
    View author publications

    You can also search for this author in PubMed Google Scholar

  7. Frank N. Mwiine
    View author publications

    You can also search for this author in PubMed Google Scholar

Contributions

SO contributed to the conception of the idea, laboratory analysis and data collection, drafting and writing of the manuscript. KVW contributed to interpretation of results and manuscript preparation. AM contributed to design and writing of the manuscript. JN contributed to laboratory analysis and writing of the manuscript. CN contributed to laboratory analysis and drafting of the manuscript. EA contributed to laboratory analysis and drafting of the manuscript. FNM contributed to conception of the idea, design and writing of the manuscript. All authors read and approved the manuscript.

Corresponding author

Correspondence to Frank N. Mwiine.

Ethics declarations

Ethics approval

The study was approved by the Institutional Animal Ethics Review Committee (SBLS/REC/13/016), Makerere University, Uganda. Oral consent was obtained from the cattle owners before their animals would be sampled.

Consent for publication

Not applicable.

Competing interests

The authors of this paper do not have any financial or personal relationship with other people or organisations that could inappropriately influence or bias the content of the paper. The authors therefore declare that they have no competing interests in the publication of this paper.

Additional information

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Additional files

Additional file 1:

Map of Uganda showing districts sampled during the FMD sero-survey (blue) and sampling sites for LSD (yellow circle) (Source of map: This study). (DOCX 275 kb)

Additional file 2:

Graph showing within herd true seroprevalence for all sampled herds and month when sampling was done. (DOCX 39 kb)

Additional file 3:

Herd/village level seroprevalence of LSD in Uganda. (DOCX 19 kb)

Rights and permissions

Open Access This article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Ochwo, S., VanderWaal, K., Munsey, A. et al. Seroprevalence and risk factors for lumpy skin disease virus seropositivity in cattle in Uganda. BMC Vet Res 15, 236 (2019). https://doi.org/10.1186/s12917-019-1983-9

Download citation

Keywords

  • Lumpy skin disease
  • Seroprevalence
  • Risk factors
  • Uganda

BMC Veterinary Research

ISSN: 1746-6148

Contact us